Abundant expression of somatic transposon-derived piRNAs throughout Tribolium castaneum embryogenesis
© The Author(s). 2017
Received: 15 November 2016
Accepted: 18 August 2017
Published: 26 September 2017
Piwi-interacting RNAs (piRNAs) are a class of short (~26–31-nucleotide) non-protein-coding RNAs expressed in the metazoan germline. The piRNA pathway in arthropods is best understood in the ovary of Drosophila melanogaster, where it acts to silence active transposable elements (TEs). Maternal loading of piRNAs in oocytes is further required for the inheritance of piRNA-mediated transposon defence. However, our understanding of the diversity, evolution and function of the piRNA complement beyond drosophilids is limited. The red flour beetle, Tribolium castaneum, is an emerging model organism separated from Drosophila by ~ 350 million years of evolution that displays a number of features ancestral to arthropods, including short germ embryogenesis. Here, we characterize the maternally deposited and zygotically expressed small RNA and mRNA complements throughout T. castaneum embryogenesis.
We find that beetle oocytes and embryos of all stages are abundant in heterogeneous ~ 28-nucleotide RNAs. These small RNAs originate from discrete genomic loci enriched in TE sequences and display the molecular signatures of transposon-derived piRNAs. In addition to the maternally loaded primary piRNAs, Tribolium embryos produce secondary piRNAs by the cleavage of zygotically activated TE transcripts via the ping-pong mechanism. The two Tribolium piRNA pathway effector proteins, Tc-Piwi/Aub and Tc-Ago3, are also expressed throughout the soma of early embryos.
Our results show that the piRNA pathway in Tribolium is not restricted to the germline, but also operates in the embryo and may act to antagonize zygotically activated transposons. Taken together, these data highlight a functional divergence of the piRNA pathway between insects.
KeywordspiRNA Short-germband development Maternal-zygotic transition Maternal transcripts Ping-pong pathway Transposons Tribolium castaneum
piRNAs are a class of short non-coding RNAs that associate with the Piwi subfamily of Argonaute proteins and are primarily involved in transcriptional and post-transcriptional silencing of transposable elements (TEs) in the germline of metazoans (reviewed in [1, 2]). Most of the current understanding of piRNA pathways in arthropods comes from studies in Drosophila melanogaster. Drosophilid genomes encode three proteins from the Piwi family—Piwi, Aubergine (Aub) and Argonaute 3 (Ago3)—all shown to be expressed in D. melanogaster gonadal tissues . Despite being structurally similar, Piwi proteins have distinct and non-redundant roles in the piRNA pathway of Drosophila. In the ovary, Piwi is expressed in both germline and somatic cells, and localizes primarily to the nucleus, where it is involved in piRNA-guided transcriptional silencing of TEs via repressive histone methylation of target loci [4–6]. Aub and Ago3 are only expressed in the germline, where they mediate post-transcriptional cleavage of active TE mRNAs in the cytoplasm [3, 7]. Analysis of the small RNAs bound to Piwi-clade proteins in Drosophila showed that Piwi and Aub associate with ~ 26 nucleotide (nt) long small RNAs biased for uracil at their 5′ end (1U) that are complementary to transposons, termed “primary piRNAs”. Most primary piRNAs derive from longer primary transcripts expressed from specialized, discrete loci in the Drosophila genome known as piRNA clusters, enriched in inactive transposons [3, 7]. In the cytoplasm, piRNA–Aub complexes cleave complementary target mRNAs at the tenth position. Secondary piRNAs produced by this cleavage have an adenine at position 10 (10A), complementary to the 1U of their primary counterparts, and are loaded into Ago3 complexes [3, 7]. The Ago3–secondary piRNA complexes recognise and cleave primary piRNA transcripts, in turn producing more primary piRNAs, thereby forming a so-called ‘ping-pong’ amplification loop [3, 7]. In contrast, the Piwi protein is expressed in both the ovarian germline and soma, and is primarily nuclear. The current model suggests that piRNA-associated Piwi is involved in co-transcriptional repression of transposons in the nucleus by directing the installation of repressive histone marks on target loci [4–6, 8–10]. Importantly, piRNAs and Piwi proteins are components of the maternally deposited pole plasm in the egg, and this deposition is required for the inheritance of the piRNA-mediated transposon response [11–13].
D. melanogaster is a classic model organism for genetic studies and developmental biology. However, the fruit fly lineage is characterized by a number of evolutionarily derived features, such as the long-germ mode of development, which is restricted to several lineages of holometabolous insects [14, 15]. As such, the piRNA pathway as observed in Drosophila might not be representative of arthropods in general. For example, in the silkworm Bombyx mori, the ‘ping-pong’ piRNA pathway has been suggested to operate not only in the germline, but also during embryogenesis . In addition, a specific piRNA has been shown to be the primary determinant of sex in this species . Furthermore, TEs are highly diverse in their types, sequences, activities and copy numbers in different species , and different transposons were shown to trigger different responses . Studies on a broader evolutionary range of organisms are vital for providing a comprehensive picture of the diversity, evolution and function of the RNA interfering pathways across the animal kingdom.
The red flour beetle Tribolium castaneum is an emerging arthropod model species, separated from Drosophila by ~ 350 million years of evolution. T. castaneum displays a number of ancestral features, including the short-germ mode of embryogenesis more typical of early development in most arthropods . T. castaneum has a fully sequenced genome and transcriptome, and a growing range of genetic and molecular techniques are available [21, 22]. Comparative genomics of RNA interfering pathway protein components has revealed that the flour beetle genome encodes two homologs of the Piwi family proteins, Tc-Piwi (the putative ortholog of Drosophila Piwi/Aub) and Tc-Ago3 . Previous studies have estimated that nearly half of the Tribolium genome is comprised of repetitive elements, including satellites and many transposons [22, 24–26]. However, the activity of these TEs, and the piRNA complement in T. castaneum, have not been investigated. We previously uncovered a highly abundant population of ~ 28-nt small RNAs that are present across T. castaneum embryonic development at levels largely exceeding those observed for microRNAs . Here, we characterize in detail the genomic and molecular properties of these small RNAs, and demonstrate that they display the molecular signatures of primary and secondary piRNAs. Temporal profiling of these small RNAs across early development shows that large numbers of primary piRNAs are pre-loaded in T. castaneum oocytes via maternal deposition. Furthermore, we observe a sharp increase in secondary piRNA-like sequences derived from exons of upregulated TE transcripts at the onset of zygotic transcription, indicating that the piRNA biogenesis pathway is responsive to active transposons during embryonic development in T. castaneum. Finally, nascent transcript in situ hybridization reveals that both Tc-Piwi/Aub and Tc-Ago3, as well as piRNA clusters, are transcribed in somatic nuclei, suggesting that the piRNA pathway is active throughout the embryo. We therefore suggest a novel role of the post-transcriptional piRNA-mediated transposon response in development of the insect embryo.
Abundant ~ 28-nt RNAs in T. castaneum embryos display the properties of piRNAs
In addition to the assembled genome, we mapped the small RNA reads to the 76 Tribolium consensus transposon sequences annotated on RepBase (v22.03) . Between 6 and 13% of small RNA reads at all developmental stages mapped to at least one of the 76 available Tribolium transposon consensus sequences. In contrast to the genome mapping, size profiles of the mapped reads showed a single peak at ~ 28 nucleotides, and no ~ 22-nt peak. Approximately 75% of the transposon-mapped reads were in antisense orientation. Nucleotide bias analysis of antisense and sense TE-mapped reads showed a strong enrichment for uracyl at the first position (1U), and adenine at the tenth position (10A), respectively, which is typical for primary and secondary piRNAs generated by the ping-pong pathway (Fig. 1b). Taken together, the maternal deposition, size, nucleotide bias and mapping to TEs strongly suggest that the ~ 28-nt RNA pool in T. castaneum embryonic samples represents piRNAs.
T. castaneum piRNAs originate from discrete genomic loci and primarily target transposons
To gain further insight into the genomic origins of the ~ 28-nt RNAs, we analysed their distribution across the T. casataneum genome. Release 4.0 of the T. castaneum genome contains ten assembled chromosomes (and a short Y chromosome) with a total length of ~ 150 Mb, and ~ 18 Mb of additional unplaced scaffolds. As the precise origins of reads mapping to multiple positions in the genome cannot be unambiguously defined, we used reads that map uniquely in our analysis (~50% of all mapped reads). Initial inspection suggested that the uniquely mapping reads originate from discrete loci, as exemplified in Fig. 1c. Using 10-kb sliding windows and 1000 25–35-nt reads per window cut-off, we identified 187 regions that are abundant sources of piRNAs, 64 of which are located on the assembled chromosomes, and the remaining 123 on the unmapped scaffolds (genome coordinates and small RNA read counts are detailed in Additional file 1). Region sizes vary between 10 and 365 kb, and encompass ~ 2% of the T. castaneum chromosomes (~3 Mb), and 15% of the unplaced scaffolds (~2.7 Mb). The top ten most piRNA-enriched regions harbour ~ 40% of all piRNAs, and together the 187 regions are a source of ~ 90% (15.9 M out of 17.9 M) of the uniquely mapped piRNA population (Fig. 1d). About 91% of the remaining piRNA-sized reads can also be mapped to these regions. Henceforth, we refer to these regions as piRNA clusters.
piRNA clusters on the assembled chromosomes are often localized in terminal chromosomal regions (Fig. 1e), which are commonly enriched for repetitive elements such as TEs . To assess the transposon content of piRNA clusters, we first annotated TEs in the T. castaneum genome assembly. RepeatMasker search identified a total of ~ 6.5 Mb homologous to known Tribolium transposons, which is consistent with previous reports [22, 25]. Note that repetitive sequences are often not assembled into available genome sequences. piRNA clusters are enriched in known transposon sequences compared to the rest of the genome: altogether, approximately 10% of all transposon annotations fall into the 3.6 Mb of the 187 piRNA clusters. Furthermore, the average transposon sequence content per kilobase within piRNA clusters is significantly higher than that for the same number of randomly sampled 1-kb windows across the genome, and the entire genome (Fig. 1f). In the T. castaneum 4.0 gene set, 740 protein-coding genes are predicted to reside in piRNA clusters. Homology searches coupled with gene ontology (GO) analysis showed that the majority are homologous to transposon-related ontology terms such as “RNA-dependent DNA replication”, “DNA integration”, etc. (Fig. 1g; Additional file 1). Thus, the majority of annotations in piRNA clusters are in fact ORFs in transposable elements. Comparisons with sequences from RepBase  show that the TEs belong to various classes, with the most widespread being retrotranspons from the gypsy family (Fig. 1h).
Temporal profiles of piRNA cluster expression and piRNA production
To understand the developmental dynamics of piRNA clusters, we determined the level of piRNA expression from each cluster during different stages of embryogenesis in a strand-specific manner (Fig. 3b). The dominant strand of the piRNA clusters remains unchanged between oocytes and different developmental stages. This suggests that either maternally deposited piRNAs are exceedingly stable, or that piRNA production from clusters is maintained throughout the course of embryonic development. In contrast, for many clusters, small RNAs from the opposite strand are not present in the maternal pool, but are upregulated at the 8–16-h time window when zygotic transcription is initiated  (Fig. 3b). Analysis of the nucleotide frequency of cluster-specific piRNAs showed that the 8–16-h time window is marked by the appearance of 10A biased piRNAs (Fig. 3c). Consistent with this, we observed a sharp increase of sense–antisense piRNA pairs with a 10-nt 5′-5′ overlap at 8–16 h and later (Fig. 3d). Such pairs are also detectable in the maternal pool but account for only ~ 3% of all piRNA reads, compared to ~ 11% at the 8–18-h stage. Together, these results show that the activation of zygotic transcription is accompanied by widespread secondary piRNA production by the ping-pong pathway.
piRNA-mediated post-transcriptional cleavage of activated TEs in the T. castaneum embryo via the ping-pong mechanism
The increase of ping-pong piRNA signatures in 8–16-h T. castaneum embryos suggests the activation of post-transcriptional cleavage of target mRNAs following the onset of zygotic transcription. To address this explicitly, we assessed the relationship between piRNA abundance and expression of piRNA targets before and after this stage, using the available total RNA-seq data from unfertilized oocytes and embryos at 8–16, 16–24 and 24–48 h developmental intervals . Normalized piRNA read counts of oocytes and 0–5-h embryos where the zygotic transcription is not yet activated were taken as a measure of “maternal” piRNA levels; “zygotic” piRNA levels were based on the read counts in libraries from 8-h embryos until hatching, where zygotic transcription is active. Maternal and zygotic mRNA expression levels were derived from the total RNA-seq data from unfertilized eggs, and the average normalised read counts in 8–48-h developmental interval samples.
Taken together, these data show that a pool of primary piRNAs antisense to TE targets is maternally deposited at high levels in the beetle and target developmentally up-regulated TE mRNAs in the post-zygotic embryo. Expression and ping-pong pathway-mediated cleavage of TEs is detectable throughout the beetle embryonic development.
A small fraction of piRNA-targeted transcripts do not show obvious similarity to TEs from the RepBase sequences, or RefSeq transcripts associated with TE-related GO terms. To address if non-TE genes are targeted by piRNAs, we examined the annotated transcripts with relatively high piRNA coverage, but no significant sequence similarity with TEs (RPKM ≥ 100; n = 130). The vast majority of the predicted ORFs in these transcripts are hypothetical proteins that do not show significant similarity with any genes of known function, and therefore their relevance is difficult to assess. While we cannot exclude the possibility that some endogenous genes produce or are targeted by piRNAs, we did not find evidence for such cases within the conserved gene set. Compelling examples of endogenous genes that produce primary piRNAs from their 3′ UTR regions similar to the Drosophila tj locus were also not identified.
Spatial expression patterns of Tc-Piwi/Aub, Tc-Ago3 and piRNA cluster transcripts indicate an active piRNA pathway in soma of the beetle embryo
Next, we used the available RNA sequencing data from unfertilized eggs and post-zygotic embryos to test whether the two Piwi subfamily members in T. castaneum, Tc-Piwi/Aub and Tc-Ago3, are actively expressed in embryos (Additional file 4: Figure S3). The data show that transcripts of these genes are maternally deposited in beetle eggs, and remain detectable throughout development. Maternally deposited mRNAs are spliced, so the presence of intronic reads in RNA sequencing data can be used to distinguish zygotically expressed transcripts . We find intronic reads for both Tc-Piwi/Aub and Tc-Ago3 in all embryonic but not in oocyte libraries, suggesting that these genes are not only maternally deposited, but actively produced during development. We then used in situ hybridization to assess the spatial expression of Tc-Piwi/Aub and Tc-Ago3 in developing embryos. To specifically detect de novo transcription, we designed RNA probes against intronic regions of the two proteins. The results show that Tc-Piwi/Aub and Tc-Ago3 are both actively transcribed in the early blastoderm (Fig. 7b). Consistent with the expression levels observed in the RNA sequencing, the peak expression of Tc-Piwi/Aub precedes that of Tc-Ago3. Interestingly, at later stages of embryogenesis the expression patterns of the two proteins appear to diverge. At the stage of blastoderm segregation, Tc-Ago3 remains highly upregulated in the cells of the germ anlage, but is not expressed in serosal nuclei. Later, Tc-Ago3 signal is detectable around the serosal window and in two distinctive bands in the middle and posterior part of the embryo. In contrast, after the uniform blastoderm stage, Tc-Piwi/Aub signal remains detectable in the serosal nuclei, but not in the embryonic body. We note that the signal obtained with the intronic probes against Tc-Piwi/Aub was generally weaker, and thus the absence of signal in embryonic cells at later stages should be treated with caution. Taken together, the evidence of active production of primary piRNAs, Tc-Piwi/Aub, Tc-Ago3 and mRNA processed into secondary piRNAs in the blastoderm, strongly suggests that the cytoplasmic piRNA pathway is active in the soma in T. castaneum.
We have explored small RNA expression in the oocytes and throughout early embryonic development of the model coleopteran T. castaneum, with a focus on understanding biogenesis and function of the piRNA pathway. The T. castaneum genome encodes two homologs of the Piwi subfamily, Tc-Ago3 and Tc-Piwi/Aub, whose transcripts are present in oocytes and actively produced in developing embryos. We identified a large fraction of diverse ~ 28-nt small RNAs that are derived from numerous discrete genomic loci enriched in TE-like sequences and display characteristics of both primary and secondary piRNAs. Although the lack of specific antibodies for Tc-Ago3 and Tc-Piwi/Aub preclude direct demonstration of small RNA loading, the developmental profile and sequence characteristics of small RNA read sequences strongly suggest that the abundant ~ 28-nt RNA fraction present throughout T. castaneum embryogenesis are piRNAs. We show that a large pool comprised of predominantly piRNAs is maternally deposited in the egg. A sharp increase of secondary piRNA production in the embryo via the ‘ping-pong’ amplification mechanism occurs at the onset of zygotic transcription and expression continues throughout the course of embryogenesis. Secondary piRNA production is correlated with TE transcriptional up-regulation in the embryo, suggesting that the piRNA pathway is functional during Tribolium embryogenesis. This contrasts with Drosophila and mammals, where the ping-pong piRNA pathway is restricted to the germline.
Functional divergence of piRNA pathway effector proteins
Comparative genomics suggests that the complement of piRNA pathway effectors have diverged between Drosophila and T. castaneum and other insects. Fruit flies encode three Piwi subfamily members, with Piwi and Aub both interacting with primary piRNAs . Other insects, including T. castaneum , Bombyx mori  and Apis mellifera , encode two members of the Piwi family, with one closely related to Piwi/Aub and the other to Ago3. Phylogenetic analysis shows that Drosophila piwi and aub are closely related to each other . Thus, it is likely that in Drosophila piwi and aub emerged by a lineage-specific duplication, after which they diversified in their subcellular localization, expression and function. In D. melanogaster, Aub is cytoplasmic and, together with Ago3, is involved in the post-transcriptional cleavage of target mRNAs in the germline via the ‘ping-pong’ mechanism [3, 7], while Piwi is expressed both in the germline and the ovarian soma [3, 32, 33]. Recent evidence suggests that Piwi is also involved in the establishment of repressive chromatin marks (H3K9me3) on target loci in the germline and somatic ovarian cells, thereby inducing transcriptional silencing [4–6]. Based on the sequence similarity to fruit fly Piwi/Aub and Ago3, and the ‘ping-pong’ post-transcriptional amplification signatures in the embryos of T. castaneum, we suggest that Tc-Piwi/Aub and Tc-Ago3 act in a similar manner to the Drosophila aub and ago3. Further studies are required to address whether the single Piwi/Aub homolog in T. castaneum and other insects also has a nuclear function. One intriguing possibility is that the high level of embryonic piRNAs and transposon expression in Tribolium is a consequence of the absence of a nuclear piRNA pathway in this species.
Spatiotemporal divergence of piRNA pathway activity
In Drosophila, the post-transcriptional cleavage of TEs and other piRNA pathway targets via the ‘ping-pong’ mechanism is active solely in the germline; piRNAs and the Piwi proteins are also maternally deposited as components of the pole plasm and present in the early embryo, but later restricted to the primordial germ cells and gonads . Our data suggest that the spatiotemporal activity of the cytoplasmic ‘ping-pong’ piRNA pathway between Drosophila and Tribolium has diverged. In Tribolium, the primary piRNA expression and the cytoplasmic ‘ping-pong’ piRNA pathway are active during early embryonic development, and we continue to detect high levels of primary and secondary piRNAs at later stages. At later stages of development, the Tc-Piwi/Aub and Tc-Ago3 expression patterns start to diverge, raising the question of how the ping-pong pathway is maintained. One possibility is that the nascent transcript FISH data do not reflect protein distribution well, and proteins produced ubiquitously in the blastoderm remain active at later stages. In addition, while the canonical ‘ping-pong’ model suggests the requirement of two distinct partners (Aub and Ago3 in Drosophila), data in mouse suggest that a single Piwi homolog, Mili, can support the post-transcriptional cleavage of target RNAs alone via the so-called ‘homotypic’ ping-pong mechanism . Thus, each piwi homolog alone could potentially support ping-pong cleavage at later developmental stages.
Similarities and differences of piRNA expression between T. castaneum and other organisms
A post-zygotic amplification of secondary piRNAs associated with transposon expression has also been reported during embryogenesis in B. mori . Taken together with our findings in T. castaneum, these data indicate that although post-transcriptional TE regulation via the ping-pong amplification mechanism in Drosophila is restricted to the gonads, the same mechanism may function during embryonic development in other insects. Drosophila, T. castaneum and B. mori belong to three different insect taxa separated by ~ 350 million years of evolution . Drosophilids are characterized by a number of evolutionarily derived features, including highly specialized embryonic development and highly derived larval structures. Thus, the zygotic secondary piRNA response in the embryo may be an ancestral state for insects that later became restricted to gonads in fruit flies. A recent report in the primitive metazoan Hydra showed that two cytoplasmic Piwi homologs are expressed in somatic stem cells, and the associated small RNAs display ‘ping-pong’ signatures , suggesting an ancient role for the cytoplasmic piRNA pathway in the soma. On the other hand, considering the burst of transposon activity in the embryos of Tribolium and Bombyx, convergent evolution of the piRNA pathway to repress their expression would not be surprising, as mutations during early development can have catastrophic effects for the organism. Finally, the Tribolium genus, B. mori and other model species such as A. mellifera, lack localized germ plasm factors and distinguishable primordial germline cells in the earliest stages of embryogenesis; these species are thought to have secondarily lost the maternally induced germline specification mechanism, and this process occurs post-zygotically instead . Thus, piRNA pathway activity in the soma of early embryos may be a feature related to a different mechanism and timing of germline specification. Indeed, the Tribolium homolog of the germline marker vasa, essential for the ping-pong pathway in both insects and vertebrates [8, 38, 39], appears to be regulated differently in the earliest stages of the beetle embryogenesis .
The spatial and temporal regulation of the Piwi pathway and piRNAs is poorly understood, and further studies at the molecular level and in other species are necessary to elucidate whether the ‘ping-pong’ piRNA response in the embryo is a conserved phenomenon or a convergent feature for T. castaneum and B. mori. Either way, investigating the regulatory mechanisms underlying the piRNA pathway similarities and differences in different species provides important clues for understanding the evolution and arms race between transposons and the RNAi interfering pathways in animals.
We characterized the piRNA and transposon expression during embryonic development of T. castaneum, an emerging model organism that undergoes an ancestral short-germ mode of embryogenesis. We found a surprisingly abundant piRNA pool throughout the entire course of beetle embryogenesis, with piRNA levels greatly exceeding these of microRNAs. The maternally deposited piRNA complement of Tribolium mainly consists of primary piRNAs. Upon the zygotic genome activation, we detect a stark increase of secondary piRNAs derived from the cleavage of zygotically upregulated transposon mRNAs via the ping-pong pathway. Further, the main effectors of the piRNA pathway, Tc-Piwi/Aub and Tc-Ago3, are also expressed in embryonic tissues. Taken together, these data show that the post-transcriptional ping-pong piRNA pathway is active during the embryonic development of Tribolium, where it counteracts activated transposons after the onset of zygotic transcription.
It is well established that the piRNA pathway has an ancient and conserved role to protect the germline genome integrity against the disruptive activity of transposable elements. Our work identifies the Tribolium embryo as a novel functional domain of the piRNA pathway in addition to its well-known activity in the germline, highlighting the spatiotemporal diversity of transposon activity and RNAi pathways among different taxa.
T. castaneum husbandry, embryo collection and in situ hybridization
Wild type T. castaneum (Michael Akam, University of Cambridge) were maintained on a mixture of whole grain flour and wheat bran supplemented with yeast at 29 °C. For embryo collection, adult beetles were paper-transferred on white flour and allowed to lay for 24 h. Embryos were separated from adults using a 300 μm sieve mesh, dechorionated in 0.5% hypochlorite solution (Sigma) and fixed in formaldehyde. Whole-mount in situ hybridization was performed using ~ 1 kb antisense dinitrophenol (DNP)- or digoxygenin (DIG)-labelled RNA probes as described previously, but omitting the proteinase K treatment step . The following forward/reverse primers were used for RNA probe synthesis:
CACACCTCGCCATTAAGACG/GAAAACCTTGGCTTGTCCCA and GCACCTTCCAACGACTGATG/GGGCAATGTTCGAGCTCAAA for the sense and antisense strand of the gypsy reverse transcriptase; CACCGAAAATCCCTTCACCGA/CCATCCAACAACGAGCAACAT for Tc-Ago intron and ATGCGAGACCATACCCAGAG/GACATCCGAGGAGTCACTTC, TGGTTGTTACACGTGCTGAA/CACATGGGCACACAAAGGAA, TACGGTTCCATGACTCGAGG/GGAAAGGAACGGTGCCAATT and TATCCGAGTTTGGGGTGAGC/TGTCATTGGTATGCACGATGT for Tc-Piwi/Aub introns.
The RNA probes were detected using rabbit anti-DNP (Life Technologies) and sheep anti-DIG primary antibodies (Roche), and anti-rabbit Alexa Fluor®647 and anti-sheep Alexa Fluor®555 secondary antibodies (Life Technologies). Images were visualized using an Olympus FV1000 confocal microscope and image stacks were processed using Fiji .
Small RNA sequencing data and data analysis
Sequencing libraries of 18–30-nt small RNA from unfertilized eggs and seven discrete T. castaneum developmental intervals were previously generated in our group and sequenced on the Illumina MiSeq or the Illumina HiSeq 2000 platform in the University of Manchester Genomic Technologies Facility, generating 50 or 150 nt long reads, respectively (GEO:GSE63770 ). Samples include oocytes and embryos at 0–5, 8–16, 16–20, 20–24, 24–34 and 34–48 h and 2–6 days following oviposition reared at 25 °C. We removed 3′ adaptor sequences using the Cutadapt tool (https://cutadapt.readthedocs.io/en/stable/), retaining reads longer than 17 nt. Trimmed reads were first filtered against tRNA sequences predicted by a tRNAscan-SE  search of the T. castaneum genome (r4.0, ftp://ftp.bioinformatics.ksu.edu/pub/BeetleBase/4.0_draft/tcas.superscaffolds.fasta) using default parameters. The remaining reads were then mapped to the same genome assembly using Bowtie 1.0  allowing one mismatch and retaining all best matches. Reads mapping to a unique position and reads mapping to multiple loci were separated. Read annotation was performed by intersection with the T. castaneum protein-coding gene annotations (r4.0) and microRNA annotations previously performed in our group [27, 45].
T. castaneum TE consensus sequences were extracted from RepBase (22.03). Small RNA mapping to TE consensuses was performed with Bowtie 1.0 allowing three mismatches, and retaining all best matches. We normalized 25–35-nt (piRNA) read counts mapping to TEs to the number of mapping positions, and to the number of unique piRNAs mapped to the genome.
For all non-TE piRNA analysis, only 25–35-nt long reads mapping to unique loci were used. Clusters were defined by merging 10-kb sliding windows containing ≥ 1000 uniquely mapping 25–35-nt reads and at least 0.0 1% coverage from pooled libraries, where those sliding windows were within 20 kb of each other. Prior to piRNA cluster definition, we excluded small RNAs mapping to ribosomal genes, as we found relatively high levels of small RNAs derived from their introns, possibly reflecting splicing intermediates. Small RNA coverage for piRNA clusters and protein-coding gene regions was calculated using the bedtools suite , and data were normalized against the total number of 25–35 nt long reads per million per kb region length (RPKM). In the case of overlapping gene annotations on the same strand, reads were split equally between the possible targets.
Nucleotide frequencies of piRNA reads at each position were calculated using a custom script, and sequence logos were plotted using the “motifStack” R package.
Ping-pong signatures were calculated following the procedure described in . In brief, we extracted 25–35-nt sense–antisense read pairs and calculated the number of overlapping pairs at each possible position. For each position, this number was scaled by the sense read counts and the antisense partner counts relative to all antisense partners overlapping at different positions, and vice versa. Data for all positions and across all pairs were summed.
Small RNA data across D. virilis development were retrieved from GEO (GSE54009).
RNA sequencing data and data analysis
Total RNA libraries from two biological replicates of T. castaneum oocytes, 8–16-h embryos (uniform blastoderm), 16–24-h embryos (gastrulation) and 24–48-h embryos (germband elongation and segmentation) were previously generated by our group using the TruSeq Stranded Total RNA Sample Prep Kit and sequenced on the Illumina HiSeq 2000 platform producing ~ 300 million 100-bp long paired-end reads (GEO: GSE63770 ). Reads were mapped to the T. castaneum genome (r4.0) using TopHat , and FPKM values were obtained from cufflinks and cuffdiff (v2.2.0) .
For mapping to the RepBase consensuses, reads from only the second mate libraries were used as single-end data. Mapping was performed with Bowtie2 using local alignment mode and allowing one mismatch in the seed region (-N 1 --local). Read counts of TEs were corrected for multiple mapping position, and normalized to the total read counts mapped to annotated transcripts.
Downstream analyses were performed using custom R and bash scripts. Heatmaps were generated using the “gplots” and “pheatmap” R packages.
Gene ontology and TE annotations
TE elements in the T. castaneum genome were identified using RepeatMasker in sensitive mode against the RepBase  database sequences, which contained 182 ancestral and ubiquitous sequences, and 64 lineage-specific sequences for this species.
The predicted protein sequences of T. castaneum transcripts (r4.0) were searched against the NCBI non-redundant protein sequences database using blastp v2.2.28+  with default parameters and an E-value cut-off of 0.001. GO annotations were obtained based on the terms assigned to the top 20 most significant hits using Blast2GO v.2.8.0 with default parameters . GO term enrichment was calculated by the Fisher’s exact test option in Blast2GO, using all transcripts as a background set. For homology to specific transposable element classes, the protein sequences were searched against RepBase v19.06  using Censor v4.2.29  with a score cut-off of 100, and the highest scoring hit was retained.
Genes displaying one or more or the following features were annotated as TE-related: presence of a RepeatMasker TE annotation within the gene sequence; significant sequence similarity to proteins with associated GO terms “transposase”, “RNA-dependent DNA replication”, “DNA integration”, “DNA recombination” (Blast2GO); Censor hits against the RepBase with score > 100.
We thank Sue Brown, Mario Stanke and Gregor Bucher for providing the T. castaneum r4.0 genome assembly and protein-coding gene annotations, and the University of Manchester Genome Technologies Facility for assistance with RNA library preparation and sequencing.
M.N. was supported by a Wellcome Trust PhD Studentship (093161/Z/10/Z).
Availability of data and material
RNA-seq datasets supporting the conclusions of this article are available in the GEO database, GSE63770 (https://www.ncbi.nlm.nih.gov/geo/query/acc.cgi?acc=GSE63770).
MN, MR and SG-J conceived the study, designed the experiments and wrote the manuscript. MN performed all experiments and data analyses and drafted the manuscript. All authors read and approved the final manuscript.
Ethics approval and consent to participate
Consent for publication
The authors declare that they have no competing interests.
Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.
Open AccessThis article is distributed under the terms of the Creative Commons Attribution 4.0 International License (http://creativecommons.org/licenses/by/4.0/), which permits unrestricted use, distribution, and reproduction in any medium, provided you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons license, and indicate if changes were made. The Creative Commons Public Domain Dedication waiver (http://creativecommons.org/publicdomain/zero/1.0/) applies to the data made available in this article, unless otherwise stated.
- Aravin A, Hannon GJ, Brennecke J. The Piwi-piRNA pathway provides an adaptive defense in the transposon arms race. Science. 2007;318:761–4.View ArticlePubMedGoogle Scholar
- Siomi MC, Sato K, Pezic D, Aravin AA. PIWI-interacting small RNAs: the vanguard of genome defence. Nat Rev Mol Cell Biol. 2011;12:246–58.View ArticlePubMedGoogle Scholar
- Brennecke J, Aravin AA, Stark A, Dus M, Kellis M, Sachidanandam R, Hannon GJ. Discrete small RNA-generating loci as master regulators of transposon activity in Drosophila. Cell. 2007;128:1089–103.View ArticlePubMedGoogle Scholar
- LeThomas A, Rogers AK, Webster A, Marinov GK, Liao SE, Perkins EM, Hur JK, Aravin AA, Tóth KF. Piwi induces piRNA-guided transcriptional silencing and establishment of a repressive chromatin state. Genes Dev. 2013;27:390–9.View ArticleGoogle Scholar
- Sienski G, Dönertas D, Brennecke J. Transcriptional silencing of transposons by Piwi and maelstrom and its impact on chromatin state and gene expression. Cell. 2012;151:964–80.View ArticlePubMedPubMed CentralGoogle Scholar
- Rozhkov NV, Hammell M, Hannon GJ. Multiple roles for Piwi in silencing Drosophila transposons. Genes Dev. 2013;27:400–12.View ArticlePubMedPubMed CentralGoogle Scholar
- Gunawardane LS, Saito K, Nishida KM, Miyoshi K, Kawamura Y, Nagami T, Siomi H, Siomi MC. A slicer-mediated mechanism for repeat-associated siRNA 5’ end formation in Drosophila. Science. 2007;315:1587–90.View ArticlePubMedGoogle Scholar
- Malone CD, Brennecke J, Dus M, Stark A, McCombie WR, Sachidanandam R, Hannon GJ. Specialized piRNA pathways act in germline and somatic tissues of the Drosophila ovary. Cell. 2009;137:522–35.View ArticlePubMedPubMed CentralGoogle Scholar
- Saito K, Inagaki S, Mituyama T, Kawamura Y, Ono Y, Sakota E, Kotani H, Asai K, Siomi H, Siomi MC. A regulatory circuit for piwi by the large Maf gene traffic jam in Drosophila. Nature. 2009;461:1296–9.View ArticlePubMedGoogle Scholar
- Li C, Vagin VV, Lee S, Xu J, Ma S, Xi H, Seitz H, Horwich MD, Syrzycka M, Honda BM, Kittler ELW, Zapp ML, Klattenhoff C, Schulz N, Theurkauf WE, Weng Z, Zamore PD. Collapse of germline piRNAs in the absence of Argonaute3 reveals somatic piRNAs in flies. Cell. 2009;137:509–21.View ArticlePubMedPubMed CentralGoogle Scholar
- Brennecke J, Malone CD, Aravin AA, Sachidanandam R, Stark A, Hannon GJ. An epigenetic role for maternally inherited piRNAs in transposon silencing. Science. 2008;322:1387–92.View ArticlePubMedPubMed CentralGoogle Scholar
- LeThomas A, Stuwe E, Li S, Du J, Marinov G, Rozhkov N, Chen Y-CA, Luo Y, Sachidanandam R, Toth KF, Patel D, Aravin AA. Transgenerationally inherited piRNAs trigger piRNA biogenesis by changing the chromatin of piRNA clusters and inducing precursor processing. Genes Dev. 2014;28:1667–80.View ArticleGoogle Scholar
- LeThomas A, Marinov GK, Aravin AA. A transgenerational process defines piRNA biogenesis in Drosophila virilis. Cell Rep. 2014;8:1–7.View ArticleGoogle Scholar
- Davis GK, Patel NH. Short, long, and beyond: molecular and embryological approaches to insect segmentation. Annu Rev Entomol. 2002;47:669–99.View ArticlePubMedGoogle Scholar
- Liu PZ, Kaufman TC. Short and long germ segmentation: unanswered questions in the evolution of a developmental mode. Evol Dev. 2005;7:629–46.View ArticlePubMedGoogle Scholar
- Kawaoka S, Arai Y, Kadota K, Suzuki Y, Hara K, Sugano S, Shimizu K, Tomari Y, Shimada T, Katsuma S. Zygotic amplification of secondary piRNAs during silkworm embryogenesis. RNA. 2011;17:1401–7.View ArticlePubMedPubMed CentralGoogle Scholar
- Kiuchi T, Koga H, Kawamoto M, Shoji K, Sakai H, Arai Y, Ishihara G, Kawaoka S, Sugano S, Shimada T, Suzuki Y, Suzuki MG, Katsuma S. A single female-specific piRNA is the primary determiner of sex in the silkworm. Nature. 2014;509:633–6.View ArticlePubMedGoogle Scholar
- Kazazian HH. Mobile elements: drivers of genome evolution. Science. 2004;303:1626–32.View ArticlePubMedGoogle Scholar
- Rahman R, Chirn G-W, Kanodia A, Sytnikova YA, Brembs B, Bergman CM, Lau NC. Unique transposon landscapes are pervasive across Drosophila melanogaster genomes. Nucleic Acids Res. 2015;43:10655–72.View ArticlePubMedPubMed CentralGoogle Scholar
- Schröder R, Beermann A, Wittkopp N, Lutz R. From development to biodiversity--Tribolium castaneum, an insect model organism for short germband development. Dev Genes Evol. 2008;218:119–26.View ArticlePubMedGoogle Scholar
- Kim HS, Murphy T, Xia J, Caragea D, Park Y, Beeman RW, Lorenzen MD, Butcher S, Manak JR, Brown SJ. BeetleBase in 2010: revisions to provide comprehensive genomic information for Tribolium castaneum. Nucleic Acids Res. 2010;38(Database issue):D437–42.View ArticlePubMedGoogle Scholar
- Richards S, Gibbs RA, Weinstock GM, Brown SJ, Denell RE, Beeman RW, Bucher G, Friedrich M, Grimmelikhuijzen CJP, Klingler M, Lorenzen M, Roth S, Schröder R, Tautz D, Zdobnov EM, Muzny D, Attaway T, Bell S, Buhay CJ, Chandrabose MN, Chavez D, Clerk-Blankenburg KP, Cree A, Dao M, Davis C, Chacko J, Dinh H, Dugan-Rocha S, Fowler G, Garner TT, et al. The genome of the model beetle and pest Tribolium castaneum. Nature. 2008;452:949–55.View ArticlePubMedGoogle Scholar
- Tomoyasu Y, Miller SC, Tomita S, Schoppmeier M, Grossmann D, Bucher G. Exploring systemic RNA interference in insects: a genome-wide survey for RNAi genes in Tribolium. Genome Biol. 2008;9:R10.View ArticlePubMedPubMed CentralGoogle Scholar
- Brajković J, Feliciello I, Bruvo-Mađarić B, Ugarković D. Satellite DNA-like elements associated with genes within euchromatin of the beetle Tribolium castaneum. G3 (Bethesda). 2012;2:931–41.View ArticleGoogle Scholar
- Wang S, Lorenzen MD, Beeman RW, Brown SJ. Analysis of repetitive DNA distribution patterns in the Tribolium castaneum genome. Genome Biol. 2008;9:R61.View ArticlePubMedPubMed CentralGoogle Scholar
- Ugarković D, Podnar M, Plohl M. Satellite DNA of the red flour beetle Tribolium castaneum--comparative study of satellites from the genus Tribolium. Mol Biol Evol. 1996;13:1059–66.View ArticlePubMedGoogle Scholar
- Ninova M, Ronshaugen M, Griffiths-jones S. MicroRNA evolution, expression, and function during short germband development in Tribolium castaneum. Genome Res. 2016;26(1):85–96.View ArticlePubMedPubMed CentralGoogle Scholar
- Jurka J, Kapitonov VV, Pavlicek A, Klonowski P, Kohany O, Walichiewicz J. Repbase Update, a database of eukaryotic repetitive elements. Cytogenet Genome Res. 2005;110:462–7.View ArticlePubMedGoogle Scholar
- Lee MT, Bonneau AR, Takacs CM, Bazzini AA, Divito KR, Fleming ES, Giraldez AJ. Nanog, Pou5f1 and SoxB1 activate zygotic gene expression during the maternal-to-zygotic transition. Nature. 2013;503:360–4.View ArticlePubMedPubMed CentralGoogle Scholar
- Kawaoka S, Minami K, Katsuma S, Mita K, Shimada T. Developmentally synchronized expression of two Bombyx mori Piwi subfamily genes, SIWI and BmAGO3 in germ-line cells. Biochem Biophys Res Commun. 2008;367:755–60.View ArticlePubMedGoogle Scholar
- Liao Z, Jia Q, Li F, Han Z. Identification of two piwi genes and their expression profile in honeybee. Apis mellifera Arch Insect Biochem Physiol. 2010;74:91–102.PubMedGoogle Scholar
- Cox DN, Chao A, Baker J, Chang L, Qiao D, Lin H. A novel class of evolutionarily conserved genes defined by piwi are essential for stem cell self-renewal. Genes Dev. 1998;12:3715–27.View ArticlePubMedPubMed CentralGoogle Scholar
- Saito K, Nishida KM, Mori T, Kawamura Y, Miyoshi K, Nagami T, Siomi H, Siomi MC. Specific association of Piwi with rasiRNAs derived from retrotransposon and heterochromatic regions in the Drosophila genome. Genes Dev. 2006;20:2214–22.View ArticlePubMedPubMed CentralGoogle Scholar
- De Fazio S, Bartonicek N, Di Giacomo M, Abreu-Goodger C, Sankar A, Funaya C, Antony C, Moreira PN, Enright AJ, O’Carroll D. The endonuclease activity of Mili fuels piRNA amplification that silences LINE1 elements. Nature. 2011;480:259–63.View ArticlePubMedGoogle Scholar
- Hedges SB, Kumar S. The timetree of life. Oxford Biol. 2009. p. 260–263.Google Scholar
- Juliano CE, Reich A, Liu N, Götzfried J, Zhong M, Uman S, Reenan RA, Wessel GM, Steele RE, Lin H. PIWI proteins and PIWI-interacting RNAs function in Hydra somatic stem cells. Proc Natl Acad Sci U S A. 2014;111:337–42.View ArticlePubMedGoogle Scholar
- Lynch JA, Ozüak O, Khila A, Abouheif E, Desplan C, Roth S. The phylogenetic origin of oskar coincided with the origin of maternally provisioned germ plasm and pole cells at the base of the Holometabola. PLoS Genet. 2011;7:e1002029.View ArticlePubMedPubMed CentralGoogle Scholar
- Kuramochi-Miyagawa S, Watanabe T, Gotoh K, Takamatsu K, Chuma S, Kojima-Kita K, Shiromoto Y, Asada N, Toyoda A, Fujiyama A, Totoki Y, Shibata T, Kimura T, Nakatsuji N, Noce T, Sasaki H, Nakano T. MVH in piRNA processing and gene silencing of retrotransposons. Genes Dev. 2010;24:887–92.View ArticlePubMedPubMed CentralGoogle Scholar
- Xiol J, Spinelli P, Laussmann MA, Homolka D, Yang Z, Cora E, Couté Y, Conn S, Kadlec J, Sachidanandam R, Kaksonen M, Cusack S, Ephrussi A, Pillai RS. RNA Clamping by Vasa assembles a piRNA amplifier complex on transposon transcripts. Cell. 2014;157:1698–711.View ArticlePubMedGoogle Scholar
- Schröder R. vasa mRNA accumulates at the posterior pole during blastoderm formation in the flour beetle Tribolium castaneum. Dev Genes Evol. 2006;216:277.View ArticlePubMedGoogle Scholar
- Kosman D, Mizutani CM, Lemons D, Cox WG, McGinnis W, Bier E. Multiplex detection of RNA expression in Drosophila embryos. Science. 2004;305:846.View ArticlePubMedGoogle Scholar
- Schindelin J, Arganda-Carreras I, Frise E, Kaynig V, Longair M, Pietzsch T, Preibisch S, Rueden C, Saalfeld S, Schmid B, Tinevez J-Y, White DJ, Hartenstein V, Eliceiri K, Tomancak P, Cardona A. Fiji: an open-source platform for biological-image analysis. Nat Methods. 2012;9:676–82.View ArticlePubMedGoogle Scholar
- Lowe TM, Eddy SR. tRNAscan-SE: a program for improved detection of transfer RNA genes in genomic sequence. Nucleic Acids Res. 1997;25:955–64.View ArticlePubMedPubMed CentralGoogle Scholar
- Langmead B, Trapnell C, Pop M, Salzberg SL. Ultrafast and memory-efficient alignment of short DNA sequences to the human genome. Genome Biol. 2009;10:R25.View ArticlePubMedPubMed CentralGoogle Scholar
- Marco A, Hui JHL, Ronshaugen M, Griffiths-Jones S. Functional shifts in insect microRNA evolution. Genome Biol Evol. 2010;2:686–96.PubMedPubMed CentralGoogle Scholar
- Quinlan AR, Hall IM. BEDTools: a flexible suite of utilities for comparing genomic features. Bioinformatics. 2010;26:841–2.View ArticlePubMedPubMed CentralGoogle Scholar
- Trapnell C, Pachter L, Salzberg SL. TopHat: discovering splice junctions with RNA-Seq. Bioinformatics. 2009;25:1105–11.View ArticlePubMedPubMed CentralGoogle Scholar
- Trapnell C, Williams BA, Pertea G, Mortazavi A, Kwan G, van Baren MJ, Salzberg SL, Wold BJ, Pachter L. Transcript assembly and quantification by RNA-Seq reveals unannotated transcripts and isoform switching during cell differentiation. Nat Biotechnol. 2010;28:511–5.View ArticlePubMedPubMed CentralGoogle Scholar
- Altschul SF, Gish W, Miller W, Myers EW, Lipman DJ. Basic local alignment search tool. J Mol Biol. 1990;215:403–10.View ArticlePubMedGoogle Scholar
- Conesa A, Götz S, García-Gómez JM, Terol J, Talón M, Robles M. Blast2GO: a universal tool for annotation, visualization and analysis in functional genomics research. Bioinformatics. 2005;21:3674–6.View ArticlePubMedGoogle Scholar
- Kohany O, Gentles AJ, Hankus L, Jurka J. Annotation, submission and screening of repetitive elements in Repbase: RepbaseSubmitter and Censor. BMC Bioinformatics. 2006;7:474.View ArticlePubMedPubMed CentralGoogle Scholar